This document was built in Markdown in R 4.0.4 and compiled on 29 March 2021. It covers package `lefko3`

version 3.4.0. Please note that this vignette was written with space considerations in mind. To reduce output size, we have prevented some statements from running if they produce long stretches of output. Examples include most `summary()`

calls. In these cases, we include hashtagged versions of these calls, and our text assumes that the user runs these statements without hashtags.

In this vignette, we use the `cypdata`

dataset to illustrate the estimation of **function-based MPMs**. Please see the other vignettes included in package `lefko3`

, as well as further vignettes posted online on the projects page of the Shefferson lab website, for further demonstrations of raw MPMs, function-based MPMs, IPMs, and age-by-stage MPMs.

The white lady’s slipper, *Cypripedium candidum*, is a North American perennial herb in the family Orchidaceae. It is long-lived and of conservation concern. The population from which the dataset originates is located within a state nature preserve located in northeastern Illinois, USA. The population was monitored annually from 2004 to 2009, with two monitoring sessions per year. Monitoring sessions took roughly 2 weeks each, and included complete censuses of the population divided into sections referred to as patches. Each monitoring session consisted of searches for previously recorded individuals, which were located according to coordinates relative to fixed stakes at the site, followed by a search for new individuals. Data recorded per individual included: the location, the number of non-flowering sprouts, the number of flowering sprouts, the number of flowers per flowering sprout, and the number of fruit pods per sprout (only in the second monitoring session per year, once fruiting had occurred). Location was used to infer individual identity. More information about this population and its characteristics is given in Shefferson et al. (2001) and Shefferson et al. (2017).

Our goal in this exercise will be to produce ahistorical and historical function-based matrices, and to compare these to see if we can spot the influence of individual history. We will also illustrate the use of multiple demographic data formats via comparison with the `cypvert`

dataset, which presents the same information as `cypdata`

but in ahistorical vertical format. Where appropriate, we will provide commentary to illustrate where analyses may be shortened or altered for more typical analyses.

Population matrix projection modeling requires an appropriate life history model showing how all stages and transitions are related. The figure below shows a very general life history model detailing these relationships in *Cypripedium candidum*. The first stage of life is a dormant seed stage, although an individual may germinate in the year following seed production. The first germinated stage is a protocorm, which is an underground, mycoheterotrophic stage unique to the families Orchidaceae and Pyrolaceae. There are three years of protocorm stages, followed by a seedling stage, and finally a set of stages that comprise the size-classified adult portion of life. The figure shows 49 such stages, each for a different number of stems (including 0 for vegetative dormancy) and one of two reproductive statuses. These stages may be reorganized for different circumstances (more on this later).

**Figure 5.1.** Life history model of *Cypripedium candidum*.

We can see a variety of transitions within this figure. The juvenile stages have fairly simple transitions. New recruits may enter the population directly from germination of a seed produced the previous year, in which case they start in the protocorm 1 stage, or they may begin as dormant seed. Dormant seed may remain dormant, die, or germinate into the protocorm 1 stage. Protocorms exist for up to 3 years, yielding the protocorm 1, 2, and 3 stages, without any possibility of staying within each of these stages for more than a single year. Protocorm 3 leads to a seedling stage, in which the plant may persist for many years before becoming mature. Here, maturity does not really refer to reproduction *per se*, but rather to a morphology indistinguishable from a reproductive plant except for the lack of a flower. The first mature stage is usually either vegetative dormancy (dorm), during which time the plant does not sprout, or a small, non-flowering adult (1V). Once in this portion of the life history, the plant may transition among 49 mature stages, including vegetative dormancy, 1-24 shoots without flowers, or 1-24 shoots with at least one flower (theoretically, individual plants may be bigger than 24 sprouts, but we have never observed a plant bigger than this in the population).

The horizontal dataset `cypdata`

, and the ahistorical vertical dataset `cypvert`

which is the same as `cypdata`

but is structured differently, both include only data for the adult stages, and so later we will need to set juvenile transitions to constants. Let’s begin by clearing the memory, loading the package, and loading the horizontal dataset.

```
rm(list=ls(all=TRUE))
library(lefko3)
data(cypdata)
```

We will first need to describe the life history characterizing the dataset, matching it to our analyses properly with a `stageframe`

for our *Cypripedium candidum* dataset. Since this analysis will be function-based, we will include all possible size classes here. If constructing raw matrices, all sizes that occur in the dataset need to be accounted for in a way that is both natural and parsimonious with respect to the numbers of individuals moving through actual transitions. If constructing function-based matrices, such as IPMs, then representative sizes at systematic increments will be satisfactory. Since size is count-based in the *Cypripedium candidum* case, we will use all numbers of stems that might occur from 0 to the maximum in the dataset, representing the life history diagram shown in the beginning of this chapter.

```
<- c(0, 0, 0, 0, 0, seq(from = 0, t = 24), seq(from = 1, to = 24))
sizevector <- c("SD", "P1", "P2", "P3", "SL", "D", "V1", "V2", "V3", "V4", "V5",
stagevector "V6", "V7", "V8", "V9", "V10", "V11", "V12", "V13", "V14", "V15", "V16", "V17",
"V18", "V19", "V20", "V21", "V22", "V23", "V24", "F1", "F2", "F3", "F4", "F5",
"F6", "F7", "F8", "F9", "F10", "F11", "F12", "F13", "F14", "F15", "F16", "F17",
"F18", "F19", "F20", "F21", "F22", "F23", "F24")
<- c(0, 0, 0, 0, 0, rep(0, 25), rep(1, 24))
repvector <- c(0, 0, 0, 0, 0, 0, rep(1, 48))
obsvector <- c(0, 0, 0, 0, 0, rep(1, 49))
matvector <- c(0, 1, 1, 1, 1, rep(0, 49))
immvector <- c(1, rep(0, 53))
propvector <- c(0, 0, 0, 0, 0, rep(1, 49))
indataset <- c("Dormant seed", "Yr1 protocorm", "Yr2 protocorm", "Yr3 protocorm",
comments "Seedling", "Veg dorm", "Veg adult 1 stem", "Veg adult 2 stems",
"Veg adult 3 stems", "Veg adult 4 stems", "Veg adult 5 stems",
"Veg adult 6 stems", "Veg adult 7 stems", "Veg adult 8 stems",
"Veg adult 9 stems", "Veg adult 10 stems", "Veg adult 11 stems",
"Veg adult 12 stems", "Veg adult 13 stems", "Veg adult 14 stems",
"Veg adult 15 stems", "Veg adult 16 stems", "Veg adult 17 stems",
"Veg adult 18 stems", "Veg adult 19 stems", "Veg adult 20 stems",
"Veg adult 21 stems", "Veg adult 22 stems", "Veg adult 23 stems",
"Veg adult 24 stems", "Flo adult 1 stem", "Flo adult 2 stems",
"Flo adult 3 stems", "Flo adult 4 stems", "Flo adult 5 stems",
"Flo adult 6 stems", "Flo adult 7 stems", "Flo adult 8 stems",
"Flo adult 9 stems", "Flo adult 10 stems", "Flo adult 11 stems",
"Flo adult 12 stems", "Flo adult 13 stems", "Flo adult 14 stems",
"Flo adult 15 stems", "Flo adult 16 stems", "Flo adult 17 stems",
"Flo adult 18 stems", "Flo adult 19 stems", "Flo adult 20 stems",
"Flo adult 21 stems", "Flo adult 22 stems", "Flo adult 23 stems",
"Flo adult 24 stems")
<- sf_create(sizes = sizevector, stagenames = stagevector,
cypframe repstatus = repvector, obsstatus = obsvector, matstatus = matvector,
propstatus = propvector, immstatus = immvector, indataset = indataset,
comments = comments)
#cypframe
```

A close look at the resulting object, `cypframe`

, shows a data frame that includes in order for each stage: the stage’s name, the associated size, its reproductive status, its status as an observable stage, its status as a propagule stage, its status as an immature stage, its status as a mature stage, whether it occurs in the dataset, the half-width of its size class bin, the minimum and maximum ages associated with the stage, the minimum and maximum of its size class bin, the centroid of its size class bin, its full size class bin width, and some text about the stage in a comments field. Stage names and combinations of characteristics must be unique to prevent estimation errors, and the comments field may be edited to include any information deemed pertinent.

Now we will transform our vertical dataset into a historically-formatted vertical file. The resulting dataset will have each individual’s observed life history broken up into states corresponding to three consecutive years per row, with plant identity marked in each row. To handle this, we use the `verticalize3()`

function, as below.

```
<- verticalize3(data = cypdata, noyears = 6, firstyear = 2004,
vertdata patchidcol = "patch", individcol = "plantid", blocksize = 4,
sizeacol = "Inf2.04", sizebcol = "Inf.04", sizeccol = "Veg.04",
repstracol = "Inf.04", repstrbcol = "Inf2.04", fecacol = "Pod.04",
stageassign = cypframe, stagesize = "sizeadded", NAas0 = TRUE)
#summary(vertdata)
```

In the above code, we described the input dataset in a way that allows R to reorganize it appropriately. For the reorganization to proceed properly, the input dataset needs to be arranged in blocks of columns for each year, with variables in the same order every year. The output dataset includes a number of summary variables, but the data is essentially broken down into groups of three consecutive monitoring occasions each (time *t*+1, *t*, and *t*-1, corresponding to `year3`

, `year2`

, and `year1`

in the output, respectively), with individuals spread across multiple rows. The output dataset is further limited to those entries in which the individual is alive in time *t* (`year2`

), meaning that all rows in which an individual is dead or not yet recruited in time *t* are dropped. Thus, we have 320 rows of data and 54 variables.

This reorganized dataset includes a set of interesting terms, the `sizeadded`

group of three variables. These are sums of the size variables for each time, such that `size1added`

is calculated as `sizea1 + sizeb1 + sizec1`

. This may or may not make sense depending on the dataset. In this particular dataset, the full size of the individual in each time is this sum, because size is determined as the number of stems per plant, and these columns give the numbers of 3 different kinds of stems: `Veg`

gives the number of non-reproductive stems, `Inf`

gives the number of single-flowered inflorescences, and `Inf2`

gives the number of double-flowered inflorescences per plant per time-step (an inflorescence takes a single stem, and no inflorescence has more than two flowers). Since size is given by the total number of stems in this example, we will use the `sizeadded`

group of variables to code individual size in our analyses.

Size and fecundity are both count variables here, and we need to determine the appropriate distribution to use in both cases. Let’s take a look at a histogram of size in time *t*.

`hist(vertdata$size2added, main = "Size in time t", xlab = "Number of stems in time t")`

We can see here that the count has a very low mean, and the curve declines fairly smoothly. The Poisson or negative binomial distribution might work for size. Before determining whether this is indeed the case, let’s also see if similar patterns hold for fecundity.

```
hist(subset(vertdata, repstatus2 == 1)$feca2, main = "Fecundity in time t",
xlab = "Number of fruit pods in time t")
```

Fecundity appears to have many 0s, suggesting the possibility that we will need to use a zero-inflated distribution.

Let’s conduct a formal test to determine the appropriate distributions for size and fecundity. The size of 0 is actually absorbed in an unobservable stage, vegetative dormancy (stage D), in this case, so we will not test for zero-inflation in the size variable. However, we will test for zero-inflation in fecundity, since fecundity is measured as the number of fruit pods produced, while all flowering individuals are treated as reproductive and so some individuals must have fecundity of 0.

```
sf_distrib(vertdata, size3 = "size3added", size2 = "size2added",
obs3 = "obsstatus3", fec = "feca2", repst = "repstatus2", zisize = FALSE)
#> The mean size is 3.653
#>
#> The variance in size is 13.41
#>
#> The probability of this dispersion level by chance assuming the true mean size = variance in size, and an alternative hypothesis of overdispersion, is 3.721e-138
#>
#> Size is significantly overdispersed.
#>
#> Mean fecundity is 0.7881
#> The variance in fecundity is 1.536
#> The probability of this dispersion level by chance assuming the true mean fecundity = variance in fecundity, and an alternative hypothesis of overdispersion, is 0.1193
#>
#> Dispersion in fecundity matches expectation.
#>
#>
#> Mean lambda is 0.4547
#> The actual number of 0s in fecundity is 68
#> The expected number of 0s in fecundity under the null hypothesis is 53.65
#> The probability of this deviation in 0s is 5.904e-06
#>
#> Fecundity is significantly zero-inflated.
#> NULL
```

The results of these tests show us that size is overdispersed. Since we have no 0s in size, we will use the zero-truncated negative binomial distribution for this vital rate. In the case of fecundity, our test for overdispersion shows that a Poisson distribution will work, but the number of 0s exceeds expectation, suggesting that it must be a zero-inflated Poisson distribution.

We may also wish to see how to proceed if our original dataset is already in vertical, but ahistorical, format. This package also includes dataset `cypvert`

, which is the same dataset as `cypdata`

but set in ahistorical vertical format. The structure of the dataset can be seen below. Note that individual histories are split across multiple rows.

**Figure 5.4.** Organization of the ahistorical vertical version of the *Cypripedium* dataset, as viewed in Microsoft Excel.

Here, we use the `historicalize3()`

function to deal with this dataset. First, let’s load the ahistorical vertical raw data file, look at its dimensions relative to the original, horizontal dataset, and finally view a summary (remove the hashtag below to run the `summary`

statement).

```
data(cypvert)
dim(cypdata)
#> [1] 77 27
dim(cypvert)
#> [1] 331 12
#summary(cypvert)
```

This dataset is longer and narrower, with more rows and fewer columns. This is because we now split data for each individual across multiple columns. After three columns of identifying information (`plantid`

, `patch`

, and `censor`

), a single column designates time in year *t*, given as `year2`

. This dataset then includes columns showing individual state in pairs of consecutive years corresponding to times *t* and *t*+1. State in time *t*-1 is not presented because this is an ahistorical dataset. This dataset includes the `plantid`

variable, which is an individual identity term that allows us to associate rows with their individuals and so allows conversion. The `historicalize3()`

function uses individual identity to reorganize datasets into historical vertical format. After the next block runs, type `summary(vertdata2)`

to get a summary of this dataset.

```
<- historicalize3(data = cypvert, patchidcol = "patch",
vertdata2 individcol = "plantid", year2col = "year2", sizea2col = "Inf2.2",
sizea3col = "Inf2.3", sizeb2col = "Inf.2", sizeb3col = "Inf.3",
sizec2col = "Veg.2", sizec3col = "Veg.3", repstra2col = "Inf2.2",
repstra3col = "Inf2.3", repstrb2col = "Inf.2", repstrb3col = "Inf.3",
feca2col = "Pod.2", feca3col = "Pod.3", repstrrel = 2, stageassign = cypframe,
stagesize = "sizeadded", censorcol = "censor", censorkeep = 1, censor = FALSE,
NAas0 = TRUE, reduce = TRUE)
#summary(vertdata2)
```

We can compare the dimensions of the new vertical datasets. The lengths of the datasets are the same in terms of rows and columns, and the variables and data are the same although the order of the columns and rows might not match (see the summaries for comparison).

```
dim(vertdata)
#> [1] 320 54
dim(vertdata2)
#> [1] 320 54
```

One important consideration is the use of censor variables. Censoring a demographic dataset refers to the elimination of suspect data points from analysis. It is typically accomplished by including a binary variable in the dataset denoting whether an individual datum is to be kept or excluded. The objects `vertdata`

and `vertdata2`

were both created without using censoring variables.However, because the datasets actually included censor variables (all data were set to be included, with no suspect data), we wished to incorporate those variables in the final datasets. Hence, although `censor = FALSE`

in both the call to `verticalize3()`

and the call to `verticalize3()`

, we also noted `censorcol = "censor"`

and `censorkeep = 1`

in the call to `historicalize3()`

. Failing to add these options to the call to `historicalize3()`

will produce the same dataset but with some zeroes entering variables `censor1`

, `censor2`

, and `censor3`

.

The next steps involve adding some external data to help parameterize the matrices properly. There are two approaches for this:

- using the
`supplemental()`

function, or - creating a reproductive matrix and using the
`overwrite()`

function.

We advise the use of the first approach, the `supplemental()`

function, which is more holistic and flexible than the other approach. However, we describe both methods below.

The `supplemental()`

function provides a means of inputting three kinds of data into MPM construction:

- fixed transition values derived from other studies and added as constants to matrices,
- proxy transition values when data for particular transitions does not exist and other, estimable transitions need to be used as proxies, and
- reproductive multipliers to indicate which stages leading to the production of which stages, and at what level relative to estimated fecundity.

Here, we create two supplement tables taking all of these sorts of data. The first is the supplement table for the historical analysis, and the second table covers the ahistorical analysis. Each row refers to a specific transition, and in the historical case, there are codes for 19 given transitions (12 for the ahistorical case). The first 9 of these transitions are set to specific probabilities, and the next 8 are transitions that will be set to other, estimated transitions (these are the non-NA transitions in `eststage`

set below). The final 2 terms of fecundity multipliers. Based on the literature, the proxies for entry into the adult classes are transitions from dormancy, as below. However, in the raw dataset, dormancy is not common enough to use as an effective proxy in raw matrix creation. Hence, we can use different proxies for function-based matrix estimation than for raw matrix estimation. Where necessary, we also use `rep`

and `mat`

as shorthand to code for all reproductive stages and all mature stages, respectively.

```
<- supplemental(stage3 = c("SD", "SD", "P1", "P1", "P2", "P3", "SL",
cypsupp3 "SL", "SL", "D", "V1", "V2", "V3", "D", "V1", "V2", "V3", "SD", "P1"),
stage2 = c("SD", "SD", "SD", "SD", "P1", "P2", "P3", "SL", "SL", "SL", "SL",
"SL", "SL", "SL", "SL", "SL", "SL", "rep", "rep"),
stage1 = c("SD", "rep", "SD", "rep", "SD", "P1", "P2", "P3", "SL", "P3", "P3",
"P3", "P3", "SL", "SL", "SL", "SL", "mat", "mat"),
eststage3 = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, "D", "V1", "V2", "V3", "D",
"V1", "V2", "V3", NA, NA),
eststage2 = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, "D", "D", "D", "D", "D",
"D", "D", "D", NA, NA),
eststage1 = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, "D", "D", "D", "D", "D",
"D", "D", "D", NA, NA),
givenrate = c(0.08, 0.08, 0.1, 0.1, 0.1, 0.1, 0.125, 0.2, 0.2, NA, NA, NA, NA,
NA, NA, NA, NA, NA, NA),
multiplier = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, NA,
NA, 0.5, 0.5),
type = c("S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S",
"S", "S", "S", "R", "R"), stageframe = cypframe)
<- supplemental(stage3 = c("SD", "P1", "P2", "P3", "SL", "SL", "D",
cypsupp2 "V1", "V2", "V3", "SD", "P1"),
stage2 = c("SD", "SD", "P1", "P2", "P3", "SL", "SL", "SL", "SL", "SL", "rep",
"rep"),
eststage3 = c(NA, NA, NA, NA, NA, NA, "D", "V1", "V2", "V3", NA, NA),
eststage2 = c(NA, NA, NA, NA, NA, NA, "D", "D", "D", "D", NA, NA),
givenrate = c(0.08, 0.1, 0.1, 0.1, 0.125, 0.2, NA, NA, NA, NA, NA, NA),
multiplier = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, NA, 0.5, 0.5),
type = c("S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "R", "R"),
stageframe = cypframe, historical = FALSE)
#cypsupp3
#cypsupp2
```

The supplement tables that we just created are the best means of adding external data to our MPMs, mostly because they allow both specific transitions to be isolated, and because they allow the use of shorthand to identify large groups of transitions (e.g. using `mat`

, `rep`

, `immat`

, `prop`

, or `all`

to signify all mature stages, reproductive stages, immature stages, propagule stages, or simply all stages, respectively). However, an alternative means is through the creation of a reproduction matrix and an `overwrite`

data frame. The reproduction matrix is an **ahistorical** matrix that tells where where fecundity rates need to be set, and at what level. *Cypripedium candidum* produces seeds that germinate by the following growing season (stage P1, or a first year protocorm), or that remain dormant for the next year (stage SD). In the following matrix, we detail that the fecundity of each reproductive stage needs to be split into two between each of these output stages. The actual split places 50% of the fecundity of a reproductive stage into each category of recruit, where the full fecundity is estimated by linear models that we will create. This reproduction matrix can be used in historical MPM construction, and it is assumed that stage at time *t*-1 is set to `all`

.

```
<- matrix(0, 54, 54)
rep.assumptions 1:2,31:54] <- 0.5
rep.assumptions[#rep.assumptions
```

Next we will create an overwrite data frame, which outlines transitions that cannot be estimated from the data set and need to be set by other means. Here is an example of two overwrite tables for the *Cypripedium candidum* analysis. Note that they are fundamentally similar to supplement tables, but neither allow the addition of fecundity multipliers nor check entered stages against the stage frame.

```
<- overwrite(stage3 = c("SD", "SD", "P1", "P1", "P2", "P3", "SL", "SL",
cypover3 "SL", "D", "V1", "V2", "V3", "D", "V1", "V2", "V3"),
stage2 = c("SD", "SD", "SD", "SD", "P1", "P2", "P3", "SL", "SL", "SL", "SL",
"SL", "SL", "SL", "SL", "SL", "SL"),
stage1 = c("SD", "rep", "SD", "rep", "SD", "P1", "P2", "P3", "SL", "P3", "P3",
"P3", "P3", "SL", "SL", "SL", "SL"),
eststage3 = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, "D", "V1", "V2", "V3", "D",
"V1", "V2", "V3"),
eststage2 = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, "D", "D", "D", "D", "D",
"D", "D", "D"),
eststage1 = c(NA, NA, NA, NA, NA, NA, NA, NA, NA, "D", "D", "D", "D", "D",
"D", "D", "D"),
givenrate = c(0.08, 0.08, 0.1, 0.1, 0.1, 0.1, 0.125, 0.2, 0.2, NA, NA, NA, NA,
NA, NA, NA, NA),
type = c("S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S", "S",
"S", "S", "S"))
<- overwrite(stage3 = c("SD", "P1", "P2", "P3", "SL", "SL", "D", "V1",
cypover2 "V2", "V3"),
stage2 = c("SD", "SD", "P1", "P2", "P3", "SL", "SL", "SL", "SL", "SL"),
eststage3 = c(NA, NA, NA, NA, NA, NA, "D", "V1", "V2", "V3"),
eststage2 = c(NA, NA, NA, NA, NA, NA, "D", "D", "D", "D"),
givenrate = c(0.08, 0.1, 0.1, 0.1, 0.125, 0.2, NA, NA, NA, NA),
type = c("S", "S", "S", "S", "S", "S", "S", "S", "S", "S"))
#cypover3
#cypover2
```

We can now proceed with matrix estimation.

Matrix creation can proceed either as raw matrix creation, as initially outlined in Ehrlén (2000), or via the creation of function-based matrices, in many ways equivalent to complex integral projection models per Ellner and Rees (2006) and as further described in the non-Gaussian case in Shefferson et al. (2014). In the raw MPM case, no vital rate models are estimated. In the function-based MPM case, vital rates are first analyzed via linear or non-linear models of the raw demographic dataset, and functions are created that estimate these vital rates according the inputs given. Matrices are then estimated using these functions, as opposed to the raw data.

Prior to vital rate estimation, a number of key decisions need to be made regarding the assumptions underlying the vital rates, and their relationships with the factors under investigation. These decisions include the **general modeling strategy**, and the **size and fecundity distributions**.

Most function-based matrices, whether integral projection models or otherwise, use either a generalized linear modeling (GLM) strategy, or a generalized linear mixed modeling (GLMM) strategy. The former is more common because of its simplicity, but the latter is theoretically more correct because it allows the user to correct for the lack of independence inherent in datasets incorporating repeat sampling from the same individuals. The difference between the two with regards to vital rate modeling is strongly related to assumptions regarding the individual and the nature of spatiotemporal variation in vital rates.

In both cases, the underlying dataset utilized is a vertical dataset. Here, each row of data gives the state of the individual in either two consecutive times (the ahistorical case), or three consecutive times (the historical case). Under a GLM framework, time is a fixed categorical variable, and individual identity is ignored. Using time as a fixed categorical variable implies that the monitoring occasions worked with are the only times for which inference is wanted. Thus, it would not be correct to infer future population dynamics after 2009 for a dataset collected between 2004 and 2009, if year is treated as fixed. Ignoring individual identity treats all transitions as independent, even though data originating from the same sampled individual is clearly not independent. This may be interpreted as a form of pseudoreplication because strongly related data is used to create matrices that are assumed to be statistically independent. In the case of linear modeling of vital rates, some of the data being used to estimate specific vital rates would originate from the same individual and so be related, even though all data points are assumed to be independent in the construction of linear models. This might impact demographic modeling by inflating Type 1 error in the linear modeling, yielding more significant terms in the chosen best-fit model.

Under a GLMM (generalized linear mixed model) framework, both time and individual identity can be treated as random categorical terms. This has two major implications. First, both time and individuals can be assumed to be random samples from a broader population of times and individuals for which inference is sought. Thus, sampled years represent a greater universe of years for which inference can be made, and so their associated coefficients can be assumed to come from a normal distribution with \(mean = 0\). Second, treating individual as a random categorical term eliminates the pseudoreplication that is inherent in the GLM approach to vital rate estimation when individuals are monitored potentially many times, because now each individual is assumed randomly drawn and associated with its own response distribution. Additionally, patch may be considered random, in which case it is assumed to have been sampled from all possible spaces that the species might occupy. We encourage researchers to use the GLMM approach in their demographic work, but we have also included easy-to-use GLM functionality, since many will find the GLM approach particularly useful in cases where mixed modeling breaks down.

Once a general approach is decided upon, the next step is to choose the underlying distributions. The probabilities of survival, observation, and reproductive status are automatically set to the binomial distribution, and this cannot be altered. However, the probability of size transition and fecundity rate can be set to the Gaussian, Poisson, or negative binomial distributions, with zero-inflated and zero-truncated versions of the Poisson and negative binomial also available. In general, if size or fecundity rate is a continuous variable (i.e., not an integer or count variable), then it should be set to the Gaussian distribution. In contrast, if size or fecundity is a count variable, then it should be set to the Poisson distribution if the mean equals the variance. The negative binomial distribution is provided in cases where the assumption that the mean equals the variance is clearly broken. We do not encourage the use of the negative binomial except in such cases, as the extra parameters estimated for the negative binomial distribution reduce the power of the modeling exercises conducted.

The Poisson and the negative binomial distributions both predict specific numbers of 0s in the response variable. If excess 0s occur within the dataset even after including the observation status and reproductive status as vital rates to absorb 0s, then a zero-inflated Poisson or negative binomial distribution may be used. These modeling approaches work by parameterizing a binomial model, typically with a logit link, to predict 0 responses. The Poisson or negative binomial is then used to predict non-zero responses. This conditional model ends up really acting as two separate models in which 0s are assumed to be predicted under potentially different processes than the remaining counts. Users should be aware that, because an extra model is built to cover 0s, zero-inflated models are much more complex and can include many more parameters than their non-inflated counterparts. The principle of parsimony suggests that they should only be used when there are significantly more 0s than expected.

Cases may arise in which 0s do not exist in either size or fecundity. For these situations, we provide zero-truncated distributions. This may occur in size if all cases of `size = 0`

are absorbed by observation status, leaving only positive integers for the size of observed individuals. For example, if an unobservable stage such as vegetative dormancy occurs and absorbs all cases of `size = 0`

, then a zero-truncated Poisson or negative binomial distribution will be more appropriate than the equivalent distribution without zero-truncation. It can also occur if all cases of `fecundity = 0`

are absorbed by reproductive status. Such distributions only involve the estimation of single, conditional models, and so are simpler than zero-inflated models.

Package `lefko3`

includes a function that can help in determining which distributions to use: `sf_distrib()`

. Earlier in this vignette, we used it to determine that we should use the zero-truncated negative binomial for size, and the zero-inflated Poisson for fecundity.

In *lefko3*, the `modelsearch`

function is the workhorse that conducts vital rate model estimation. Here, we will create a full suite of vital rate models for the *Cypripedium candidum* dataset. Before proceeding, we need to decide on the linear model building strategy, the correct vital rates to model, the proper statistical distributions for estimated vital rates, the proper parameterizations for each vital rate, and the strategy for determination of the best-fit models.

First, we must determine the model building strategy. In most cases, the best procedure will be through mixed linear models in which monitoring occasion and individual identity are random terms. We will set monitoring occasion as random because we wish to make inferences for the population as a whole and do not wish to restrict ourselves to inference only for the years monitored (i.e. our distribution of years sampled is itself a sample of the population in time). We will set individual identity as random because many or most of the individuals that we have sampled to produce our dataset yield multiple observation data points across time. Thus, we will use `approach = "mixed"`

in the parameterization for `modelsearch`

. To make sure that time and individual identity are treated as random, we just need to set the proper variable names for `indiv`

and `year`

, which correspond to individual identity (`individ`

by default), and to time *t* (`year2`

by default). The `year.as.random`

option is set to random by default, and leaving it this way also means that R will randomly draw coefficient values for years with inestimable coefficients. Setting `year.as.random`

to FALSE would make time a fixed variable.

The mixed modeling approach is usually preferable to the GLM approach, particularly because it allows us to handle data points originating from the same individual as related. However, a mixed modeling strategy results in lower statistical power and a greater time used in estimating models. Users of package `lefko3`

wishing to use a standard generalized linear modeling strategy can set `approach = "glm"`

. In this case, individual identity is not used, time is a fixed factor, and all observed transitions are treated as independent.

Next, we must determine which vital rates to model. Function `modelsearch()`

estimates up to 9 vital rate models:

survival probability from time

*t*to time*t*+1,observation probability in time

*t*+1 assuming survival until that time,size in time

*t*+1 assuming survival and observation in that time,reproduction status in time

*t*+1 assuming survival and observation until that time,fecundity rate assuming survival in time

*t*and observation and reproduction in time*t*+1 (mature only),juvenile survival probability from time

*t*to time*t*+1,juvenile observation probability in time

*t*+1 assuming survival until that time,juveile size in time

*t*+1 assuming survival and observation in that time, andreproduction status in time

*t*+1 assuming survival and observation until that time of a juvenile in time*t*that is becoming mature in time*t*+1.

The default settings for `modelsearch`

estimate 1) survival probability, 3) size distribution, and 5) fecundity, which are the minimum 3 vital rates required for a full projection matrix. Observation probability (option `obs`

in `vitalrates`

) should only be included when a life history stage or size exists that cannot be observed. For example, in the case of a plant with vegetative dormancy, the observation probability can be thought of as the sprouting probability, which is a biologically meaningful vital rate (Shefferson et al. 2001). Further, reproduction status (option `repst`

in `vitalrates`

) should only be modeled if size classification needs to be stratified by the ability to reproduce, as when 0 fecundity occurs within stages that also produce offspring. In this latter case, we can imagine that reproductive and non-reproductive individuals of each size class might theoretically exist, and we may wish to parameterize transitions allowing individuals to be reproductive or non-reproductive. Since *Cypripedium candidum* is capable of long bouts of vegetative dormancy, since we wish to stratify the population into reproductive and non-reproductive adults of the same size classes, and since we have no data derived from juvenile individuals, we will set `vitalrates = c("surv", "obs", "size", "repst", "fec")`

.

Third, we need to set the proper statistical distribution for each parameter. Survival probability, observation probability, and reproductive status are all modeled as binomial variables, and this cannot be changed. In the case of this population of *Cypripedium candidum*, size was measured as the number of stems and so is a count variable. Likewise, fecundity is actually estimated as the number of fruits produced per plant, and so is also a count variable. We have already performed tests for overdispersion and zero-inflation, and we are also aware that size in observed stages cannot be 0, requiring zero truncation in that parameter. So we will set size to the zero-truncated negative binomial distribution, and fecundity to the zero-inflated Poisson distribution.

Fourth, we need the proper model parameterizations for each vital rate, using the `suite`

option. The default, `suite = "main"`

, under the mixed model setting (`approach = "mixed"`

) starts with the estimation of global models that include size in times *t* and *t*-1, and reproductive status in times *t* and *t*-1, as fixed factors, with individual identity and time *t* set as random terms in a mixed model framework. Other terms can be included when specified, such as individual covariates and age. Setting `suite = "full"`

will yield global models that also include all two-way interactions. We will set it to the latter. The default under the GLM setting (`approach = "glm"`

) makes time *t* a fixed term and drops individual identity from consideration. The global model under `suite = "full"`

then includes all fixed factors noted before, plus time *t* and all two-way interactions with it. If the population is not stratified by reproductive status, then `suite = "size"`

will eliminate reproductive status terms and use all others in the global model. If size is not important, then `suite = "rep"`

will eliminate size but keep reproductive status and all other terms. Finally, `suite = "cons"`

will result in a global model in which neither reproductive status nor size are considered.

Fifth, and finally, we need to determine the proper strategy for the determination of the best-fit model. Model building proceeds through the `dredge`

function in package `MuMIn`

(Barton 2014), and each model has an associated AICc value. The default setting in `lefko3`

(`bestfit = "AICc&k"`

) will compare all models within 2.0 AICc units of the model with \(\Delta AICc = 0\), and choose the one with the lowest degrees of freedom. This approach is generally better than the alternative, which simply uses the model with \(\Delta AICc = 0\) (`bestfit = "AICc"`

), as all models within 2.0 AICc units of that model are equally parsimonious and so fewer degrees of freedom result from fewer parameters estimated (Burnham and Anderson 2002).

In the model building exercise below, we will use the `suite = "full"`

option to run all main effects and their two-way interactions. Once done, we can summarize the output with the `summary()`

function.

```
<- modelsearch(vertdata, historical = TRUE, approach = "mixed",
cypmodels3 vitalrates = c("surv", "obs", "size", "repst", "fec"), sizedist = "negbin",
size.trunc = TRUE, fecdist = "poisson", fec.zero = TRUE, suite = "full",
size = c("size3added", "size2added", "size1added"), quiet = TRUE)
#> boundary (singular) fit: see ?isSingular
#> Warning in checkConv(attr(opt, "derivs"), opt$par, ctrl = control$checkConv, : Model failed to converge with max|grad| = 0.00275551 (tol =
#> 0.002, component 1)
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in fitTMB(TMBStruc): Model convergence problem; non-positive-definite Hessian matrix. See vignette('troubleshooting')
#> Warning in checkConv(attr(opt, "derivs"), opt$par, ctrl = control$checkConv, : Model failed to converge with max|grad| = 0.0099624 (tol =
#> 0.002, component 1)
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#summary(cypmodels3)
```

As `modelsearch`

works, it produces a good amount of text to allow the user to understand what is going on. It is entirely possible, and actually quite likely, that many warning messages will appear, and these may be of use in understanding the dataset and how well it conforms to analytical assumptions. We have silenced most of this with the `quiet = TRUE`

option, although some red text still indicates a few warnings that have slipped through. These are not to be terribly concerned about. However, we encourage users to allow the function to run unsilenced in case of modeling problems. Please read the documentation for functions `lm`

, `glm`

, `glm.nb`

, `lmer`

(lme4 package), `glmer`

(lme4 package), `glmmTMB`

(glmmTMB package), `zeroinfl`

(pscl package), `vglm`

(VGAM package), and `dredge`

(MuMIn package) for further information on the sources of problems in such models. Note, however, that some warnings are expected, and so are not cause for alarm.

In the output, we see historical terms determining size, suggesting that we cannot ignore history. The `summary`

function gives us a great deal of information about all of the models, but also hides a number of more technical details. For example, the complete model selection tables are actually included in the `modelsearch`

output, and users can see these by calling them directly. For example, type `cypmodels3$survival_table`

at the prompt to examine the model table for survival.

Before moving on, we note that the models created above are actually only usable for the construction of historical models. For comparison, we may wish to estimate ahistorical models. In that case, we also need linear models in which the global models tested do not include state at time *t*-1. Here, we produce these models.

```
<- modelsearch(vertdata, historical = FALSE, approach = "mixed",
cypmodels2 vitalrates = c("surv", "obs", "size", "repst", "fec"), sizedist = "negbin",
size.trunc = TRUE, fecdist = "poisson", fec.zero = TRUE, suite = "full",
size = c("size3added", "size2added"), quiet = TRUE)
#> Warning in checkConv(attr(opt, "derivs"), opt$par, ctrl = control$checkConv, : Model failed to converge with max|grad| = 0.0330464 (tol =
#> 0.002, component 1)
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#> Warning in Matrix::sparseMatrix(dims = c(0, 0), i = integer(0), j = integer(0), : 'giveCsparse' has been deprecated; setting 'repr = "T"' for
#> you
#summary(cypmodels2)
```

Fewer models were estimated per dredge, since fewer parameters were tested in the global models (size and reproductive status in time *t*-1 were not included). So, the best-fit models should look a little bit different. However, a more thorough comparison will show that many of the best-fit models are similar between historical and ahistorical analysis. This is not guaranteed - in this case, it may be that the relatively small number of years and small overall sample size leaves too little power to find an impact of historical status on most vital rates. However, with size impacted by history, the choice of a historical model is better here.

Now we will create function-based MPMs. Function-based matrices have been taking over in population ecology, probably because of their ability to parse out interesting trends and influential factors picked up by the linear modeling of vital rates. Most of these are integral projection models, which involve the creation of many fine-scale size bins to capture the variation in a continuous size metric. However, function-based matrices can also be developed for organisms in which size is measured using a count variable. That is what we will do here. Let’s first create a set of ahistorical matrices.

```
<- flefko2(stageframe = cypframe, supplement = cypsupp2,
cypmatrix2 modelsuite = cypmodels2, data = vertdata, year.as.random = TRUE)
summary(cypmatrix2)
#>
#> This ahistorical lefkoMat object contains 5 matrices.
#>
#> Each matrix is a square matrix with 54 rows and columns, and a total of 2916 elements.
#> A total of 12055 survival transitions were estimated, with 2411 per matrix.
#> A total of 240 fecundity transitions were estimated, with 48 per matrix.
#>
#> Vital rate modeling quality control:
#>
#> Survival estimated with 74 individuals and 320 individual transitions.
#> Observation estimated with 70 individuals and 303 individual transitions.
#> Size estimated with 70 individuals and 288 individual transitions.
#> Reproductive status estimated with 70 individuals and 288 individual transitions.
#> Fecundity estimated with 51 individuals and 118 individual transitions.
#> Juvenile survival not estimated.
#> Juvenile observation probability not estimated.
#> Juvenile size transition not estimated.
#> Juvenile reproduction probability not estimated.
#> NULL
```

A quick glance at the summary output will highlight that many more elements are estimated for function-based matrices than for raw matrices - this time 2,459 out of 2,916 total elements (84.3%). In raw matrices, elements associated with transitions from specific stages are only estimated when individuals actually exist within those particular stages. In function-based matrices, in contrast, the linear models estimated allow the estimation of all elements that are theoretically possible (i.e. only structural 0s are not estimated).

The matrices are overwhelmingly composed of non-zero elements, unlike raw ahistorical matrices. The output of the `flefko2()`

call includes several key elements. One of the most important is a data frame showing the order of matrices produced. Let’s take a look at this object for `cypmatrix2`

.

```
$labels
cypmatrix2#> pop patch year2
#> 1 1 1 2004
#> 2 1 1 2005
#> 3 1 1 2006
#> 4 1 1 2007
#> 5 1 1 2008
```

Here we see that our 5 matrices are annual matrices all corresponding to the same population/patch. Other elements in this object include summaries of the stages used, in the order that they occur in the matrix. Since this is an ahistorical MPM, the key element here is `cypmatrix2$ahstages`

. If this were a historical MPM, then this stages would give the order of stages, but `cypmatrix2$hstages`

includes the order of stage-pairs corresponding to the rows and columns in such MPMs.

Before moving on, we can also create the same matrices using the overwrite tables and reproduction matrix. Here is an example, with a summary.

```
<- flefko2(stageframe = cypframe, overwrite = cypover2,
cypmatrix2_alt repmatrix = rep.assumptions, modelsuite = cypmodels2, data = vertdata,
year.as.random = TRUE)
summary(cypmatrix2_alt)
#>
#> This ahistorical lefkoMat object contains 5 matrices.
#>
#> Each matrix is a square matrix with 54 rows and columns, and a total of 2916 elements.
#> A total of 12055 survival transitions were estimated, with 2411 per matrix.
#> A total of 240 fecundity transitions were estimated, with 48 per matrix.
#>
#> Vital rate modeling quality control:
#>
#> Survival estimated with 74 individuals and 320 individual transitions.
#> Observation estimated with 70 individuals and 303 individual transitions.
#> Size estimated with 70 individuals and 288 individual transitions.
#> Reproductive status estimated with 70 individuals and 288 individual transitions.
#> Fecundity estimated with 51 individuals and 118 individual transitions.
#> Juvenile survival not estimated.
#> Juvenile observation probability not estimated.
#> Juvenile size transition not estimated.
#> Juvenile reproduction probability not estimated.
#> NULL
```

The general details are essentially the same. However, it is important to note that the supplement table approach allows both more flexibility and a greater detail in designating transitions, particularly historical fecundity. These differences may result in some differences in matrices between these approaches, particularly in historical MPMs. We encourage the use of supplement tables instead of overwrite tables and reproduction matrices.

Next, we will create a set of historical Lefkovitch matrices.

```
<- flefko3(stageframe = cypframe, supplement = cypsupp3,
cypmatrix3 modelsuite = cypmodels3, data = vertdata, yearcol = "year2",
year.as.random = TRUE)
summary(cypmatrix3)
#>
#> This historical lefkoMat object contains 5 matrices.
#>
#> Each matrix is a square matrix with 2916 rows and columns, and a total of 8503056 elements.
#> A total of 588560 survival transitions were estimated, with 117712 per matrix.
#> A total of 11760 fecundity transitions were estimated, with 2352 per matrix.
#>
#> Vital rate modeling quality control:
#>
#> Survival estimated with 74 individuals and 320 individual transitions.
#> Observation estimated with 70 individuals and 303 individual transitions.
#> Size estimated with 70 individuals and 288 individual transitions.
#> Reproductive status estimated with 70 individuals and 288 individual transitions.
#> Fecundity estimated with 51 individuals and 118 individual transitions.
#> Juvenile survival not estimated.
#> Juvenile observation probability not estimated.
#> Juvenile size transition not estimated.
#> Juvenile reproduction probability not estimated.
#> NULL
```

Once again, we see many more elements estimated (over 8.5 million, in comparison to 2,916 in the ahistorical case), and many more rows and columns (54 rows and columns in the ahistorical case, and 54^{2} = 2,916 rows and columns in the historical case). However, the dominance of structural 0s in historical matrices still yields matrices that are mostly composed of 0s. In this case, with only 120,064 elements estimated per matrix, only 1.4% of elements are non-zero (the equivalent percentage for the ahistorical case is 84.3%).

Now let’s estimate some element-wise mean matrices. First, we will create the ahistorical mean matrix. We will also very quickly calculate the column sums, which represent the actual survival of stages from time *t* to time *t*+1. Column sums are very useful to make sure that no errors have resulted in odd values, such as overall survival probabilities greater than 1.0.

```
<- lmean(cypmatrix2)
tmeans2r summary(colSums(tmeans2r$U[[1]]))
#> Min. 1st Qu. Median Mean 3rd Qu. Max.
#> 0.1000 0.9910 0.9999 0.9251 1.0000 1.0000
```

Column sums are very useful tools in checking yourself, because they are equal to the overall annual survival of the stage (for ahistorical MPM) in question, or the stage-pair (for historical MPM) in question. The use of externally-supplied rates and probabilities, as supplied via the supplement and overwrite tables, can result in some stages or stage-pairs having survival probabilities greater than 1.0, and if that occurs, then the supplement/overwrite tables need to be corrected to bring survival down to something reasonable. Further, some aspects of vital rate modeling may result in odd probabilities, including survival probabilities greater than 1.0, yielding situations in which background distributions or other assumptions must be changed, In our case, since we do not have juvenile data for *Cypripedium candidum*, we need to make sure that all is well in this regard before proceeding.

Next we will estimate the historical element-wise mean matrix, along with its column sums (these represent the survival of stage pairs in time *t*-1 and time *t*).

```
<- lmean(cypmatrix3)
tmeans3r summary(colSums(tmeans3r$U[[1]]))
#> Min. 1st Qu. Median Mean 3rd Qu. Max.
#> 0.0000 0.9646 0.9998 0.8189 1.0000 1.0000
```

It might help to do a more holistic comparison of the ahistorical vs. historical MPMS. Let’s do matrix plots of the ahistorical and historical means. For this purpose, we will use the `image3()`

function. Let’s first view the ahistorical matrix image.

`image3(tmeans2r, used = 1)`

`#> NULL`

This is a fairly large matrix, and rather dense though with obviously large clusters of zero elements particularly at the edges. Now let’s see the historical matrix.

`image3(tmeans3r, used = 1)`

`#> NULL`

Historical matrices are often huge and always sparse, just as our historical matrix is in the plot above. Although there are roughly 8.5 million elements, very few are non-zero and those are identified as the red streaks in the matrix image above. The ahistorical matrix is large and somewhat sparse for an ahistorical matrix, but tiny and quite dense relative to the historical matrix above.

For further comparison, let’s decompose the mean historical matrix into conditional historical matrices. We’ll take a look at the matrix conditional on being vegetatively dormant in time *t*-1 (remember to remove the hashtag to see this conditional matrix).

```
<- cond_hmpm(tmeans3r)
condm3r #print(condm3r$Acond[[1]]$D, digits = 3)
```

Let’s move on to some of the analyses that are currently possible with `lefko3`

.

Let’s now conduct some quick population analyses. First, we can estimate the deterministic and stochastic population growth rates for these means. The use of `set.seed`

is to make our stochastic results reproducible.

```
set.seed(42)
<- slambda3(cypmatrix2)
cypann2s <- slambda3(cypmatrix3)
cypann3s
lambda3(tmeans2r)
#> pop patch lambda
#> 1 1 1 0.9566419
lambda3(tmeans3r)
#> pop patch lambda
#> 1 1 1 0.9570233
cypann2s#> pop patch a var sd se
#> 1 1 1 -0.04427222 0.002857724 0.05345769 0.0005345769
cypann3s#> pop patch a var sd se
#> 1 1 1 -0.04389879 0.002821212 0.05311509 0.0005311509
```

The \(\lambda\) values are similar to one another, as are estimates of \(a = \text{log} \lambda _{S}\), although the historical is slightly larger than the ahistorical in both cases. Let’s take a look at a plot of annual deterministic growth rates (stochastic growth rate is calculated across time so is not included).

```
<- lambda3(cypmatrix3)
cypann3 <- lambda3(cypmatrix2)
cypann2
plot(lambda ~ year2, data = cypann2, xlab = "Year", ylab = "Lambda", ylim = c(0.93, 0.98), type = "l", lty= 1, lwd = 2, bty = "n")
lines(lambda ~ year2, data = cypann3, lty = 2, lwd= 2, col = "red")
legend("bottomright", c("ahistorical", "historical"), lty = c(1, 2), col = c("black", "red"), lwd = 2, bty = "n")
```

We find that annual \(\lambda\) estimates differ only slightly between ahistorical and historical analyses.

Now let’s take a look at the stable stage distributions. We will look at deterministic and stochastic versions of the ahistorical and historical MPMs.

```
<- stablestage3(tmeans2r)
tm2ss <- stablestage3(tmeans3r)
tm3ss <- stablestage3(cypmatrix2, stochastic = TRUE, seed = 42)
tm2ss_s <- stablestage3(cypmatrix3, stochastic = TRUE, seed = 42)
tm3ss_s
<- cbind.data.frame(tm2ss$ss_prop, tm3ss$ahist$ss_prop,
ss_put_together $ss_prop, tm3ss_s$ahist$ss_prop)
tm2ss_snames(ss_put_together) <- c("det ahist", "det hist", "sto ahist", "sto hist")
rownames(ss_put_together) <- tm2ss$stage_id
barplot(t(ss_put_together), beside=T, ylab = "Proportion", xlab = "Stage",
ylim = c(0, 0.15), col = c("black", "orangered", "grey", "darkred"), bty = "n")
legend("topright", c("det ahist", "det hist", "sto ahist", "sto hist"),
col = c("black", "orangered", "grey", "darkred"), pch = 15, bty = "n")
```

Overall, these are very similar patterns. Both suggest that small non-reproductive adults take up the greatest share of the stable stage structure, with dormant seed and 1st-year protocorms coming next, and then reproductive adults. The main differences appear to be a decreased presence of protocorms and increased presence of flowering adults in historical analysis. Stochastic analyses also reduce the importance of most stages with high proportions, while increasing the importance of rarer stages.

Next let’s look at the reproductive values associated with both ahistorical and historical approaches. We will standardize against the maximum value in each case to make these comparable.

```
<- repvalue3(tmeans2r)
tm2rv <- repvalue3(tmeans3r)
tm3rv <- repvalue3(cypmatrix2, stochastic = TRUE, seed = 42)
tm2rv_s <- repvalue3(cypmatrix3, stochastic = TRUE, seed = 42)
tm3rv_s
<- cbind.data.frame((tm2rv$rep_value / max(tm2rv$rep_value)),
rv_put_together $ahist$rep_value / max(tm3rv$ahist$rep_value)),
(tm3rv$rep_value / max(tm2rv_s$rep_value)),
(tm2rv_s$ahist$rep_value / max(tm3rv_s$ahist$rep_value)))
(tm3rv_snames(rv_put_together) <- c("det ahist", "det hist", "sto ahist", "sto hist")
rownames(rv_put_together) <- tm2rv$stage_id
barplot(t(rv_put_together), beside=T, ylab = "Relative rep value", xlab = "Stage",
ylim = c(0, 1.3), col = c("black", "orangered", "grey", "darkred"), bty = "n")
legend("topleft", c("det ahist", "det hist", "sto ahist", "sto hist"),
col = c("black", "orangered", "grey", "darkred"), pch = 15, bty = "n")
```

We see some big differences here. In the deterministic analyses, the historical case predicts a greater importance of small and medium-sized flowering adults, and a lower importance of all other stages than the ahistorical case. In the stochastic analyses, the highest reproductive values are in the largest flowering adults. So, both history and temporal stochasticity have large effects here. Interesting results in need of further study!

Let’s now do a sensitivity analysis, again using both deterministic and stochastic approaches.

```
<- sensitivity3(tmeans2r)
tm2sens <- sensitivity3(cypmatrix2, stochastic = TRUE, seed = 42)
tm2sens_s
writeLines("\nThe highest deterministic sensitivity value: ")
#>
#> The highest deterministic sensitivity value:
max(tm2sens$ah_sensmats[[1]][which(tmeans2r$A[[1]] > 0)])
#> [1] 0.217052
writeLines("\nThis value is associated with element: ")
#>
#> This value is associated with element:
which(tm2sens$ah_sensmats[[1]] == max(tm2sens$ah_sensmats[[1]][which(tmeans2r$A[[1]] > 0)]))
#> [1] 378
writeLines("\nThe highest stochastic sensitivity value: ")
#>
#> The highest stochastic sensitivity value:
max(tm2sens_s$ah_sensmats[[1]][which(tmeans2r$A[[1]] > 0)])
#> [1] 0.2262888
writeLines("\nThis value is associated with element: ")
#>
#> This value is associated with element:
which(tm2sens_s$ah_sensmats[[1]] == max(tm2sens_s$ah_sensmats[[1]][which(tmeans2r$A[[1]] > 0)]))
#> [1] 378
```

The highest sensitivity value in both cases appears to be associated with the transition from 1-sprouted non-flowering adult to the largest non-flowering adult. Inspecting each sensitivity matrix also shows that transitions near that element in both matrices are also associated with rather high sensitivities.

Now let’s compare with the historical case. We will compare both the full historical sensitivity matrices, and also look at the historically-corrected deterministic sensitivities (these are not currently available for stochastic sensitivities).

```
<- sensitivity3(tmeans3r)
tm3sens <- sensitivity3(cypmatrix3, stochastic = TRUE, see = 42)
tm3sens_s
writeLines("\nThe highest deterministic sensitivity value: ")
#>
#> The highest deterministic sensitivity value:
max(tm3sens$h_sensmats[[1]][which(tmeans3r$A[[1]] > 0)])
#> [1] 0.05718035
writeLines("\nThis value is associated with element: ")
#>
#> This value is associated with element:
which(tm3sens$h_sensmats[[1]] == max(tm3sens$h_sensmats[[1]][which(tmeans3r$A[[1]] > 0)]))
#> [1] 962658
writeLines("\nThe highest stochastic sensitivity value: ")
#>
#> The highest stochastic sensitivity value:
max(tm3sens_s$h_sensmats[[1]][which(tmeans3r$A[[1]] > 0)])
#> [1] 0.05983271
writeLines("\nThis value is associated with element: ")
#>
#> This value is associated with element:
which(tm3sens_s$h_sensmats[[1]] == max(tm3sens_s$h_sensmats[[1]][which(tmeans3r$A[[1]] > 0)]))
#> [1] 962658
writeLines("\nThe highest deterministic sensitivity value (historically-corrected): ")
#>
#> The highest deterministic sensitivity value (historically-corrected):
max(tm3sens$ah_sensmats[[1]][which(tmeans2r$A[[1]] > 0)])
#> [1] 0.2160675
writeLines("\nThis value is associated with element: ")
#>
#> This value is associated with element:
which(tm3sens$ah_sensmats[[1]] == max(tm3sens$ah_sensmats[[1]][which(tmeans2r$A[[1]] > 0)]))
#> [1] 374
```

Here, we see both deterministic and stochastic sensitivity analyses supporting the transition from 1-sprouted vegetative adult in times *t*-1 and *t* to the largest flowering adult in time *t*+1. The highest historically-corrected sensitivity value is associated with the transition from 1-sprouted non-flowering adult to 20-sprouted flowering adults. Thus, our results reinforce the results of the ahistorical case.

Let’s now assess the elasticity of \(\lambda\) to matrix elements, comparing the ahistorical to the historically-corrected case in both deterministic and stochastic analyses.

```
<- elasticity3(tmeans2r)
tm2elas <- elasticity3(tmeans3r)
tm3elas <- elasticity3(cypmatrix2, stochastic = TRUE, seed = 42)
tm2elas_s <- elasticity3(cypmatrix3, stochastic = TRUE, seed = 42)
tm3elas_s
writeLines("\nThe largest ahistorical deterministic elasticity is associated with element: ")
#>
#> The largest ahistorical deterministic elasticity is associated with element:
which(tm2elas$ah_elasmats[[1]] == max(tm2elas$ah_elasmats[[1]]))
#> [1] 331
writeLines("\nThe largest historically-corrected deterministic elasticity is associated with element: ")
#>
#> The largest historically-corrected deterministic elasticity is associated with element:
which(tm3elas$ah_elasmats[[1]] == max(tm3elas$ah_elasmats[[1]]))
#> [1] 331
writeLines("\nThe largest historical deterministic elasticity is associated with element: ")
#>
#> The largest historical deterministic elasticity is associated with element:
which(tm3elas$h_elasmats[[1]] == max(tm3elas$h_elasmats[[1]]))
#> [1] 962611
writeLines("\nThe largest ahistorical stochastic elasticity is associated with element: ")
#>
#> The largest ahistorical stochastic elasticity is associated with element:
which(tm2elas_s$ah_elasmats[[1]] == max(tm2elas_s$ah_elasmats[[1]]))
#> [1] 331
writeLines("\nThe largest historically-corrected stochastic elasticity is associated with element: ")
#>
#> The largest historically-corrected stochastic elasticity is associated with element:
which(tm3elas_s$ah_elasmats[[1]] == max(tm3elas_s$ah_elasmats[[1]]))
#> [1] 331
writeLines("\nThe largest historical stochastic elasticity is associated with element: ")
#>
#> The largest historical stochastic elasticity is associated with element:
which(tm3elas_s$h_elasmats[[1]] == max(tm3elas_s$h_elasmats[[1]]))
#> [1] 962611
```

Ahistorical and historical, deterministic and stochastic analyses suggest that population growth rate is most elastic in response to stasis as 1-sprouted non-flowering adult. This is a remarkably consistent result, reinforcing the importance of this stage as seen in sensitivity analyses.

Now let’s compare the elasticity of population growth rate in relation to the core life history stages, via a barplot comparison.

```
<- cbind.data.frame(colSums(tm2elas$ah_elasmats[[1]]),
elas_put_together colSums(tm3elas$ah_elasmats[[1]]), colSums(tm2elas_s$ah_elasmats[[1]]),
colSums(tm3elas_s$ah_elasmats[[1]]))
names(elas_put_together) <- c("det ahist", "det hist", "sto ahist", "sto hist")
rownames(elas_put_together) <- tm2elas$ah_stages$stage_id
barplot(t(elas_put_together), beside=T, ylab = "Elasticity", xlab = "Stage",
col = c("black", "orangered", "grey", "darkred"), bty = "n")
legend("topright", c("det ahist", "det hist", "sto ahist", "sto hist"),
col = c("black", "orangered", "grey", "darkred"), pch = 15, bty = "n")
```

Elasticity analyses in these plots look fairly similar, with most of the differences appearing to lie in elasticity of small non-flowering vs. flowering adults in the ahistorical vs. historical comparison.

Finally, let’s take a look at how the importance of different kinds of transitions changes, by looking at elasticity sums.

```
<- summary(tm2elas)
tm2elas_sums <- summary(tm3elas)
tm3elas_sums <- summary(tm2elas_s)
tm2elas_s_sums <- summary(tm3elas_s)
tm3elas_s_sums
<- cbind.data.frame(tm2elas_sums$ahist[,2],
elas_sums_together $ahist[,2], tm2elas_s_sums$ahist[,2], tm3elas_s_sums$ahist[,2])
tm3elas_sumsnames(elas_sums_together) <- c("det ahist", "det hist", "sto ahist", "sto hist")
rownames(elas_sums_together) <- tm2elas_sums$ahist$category
barplot(t(elas_sums_together), beside=T, ylab = "Elasticity", xlab = "Transition",
col = c("black", "orangered", "grey", "darkred"), bty = "n")
legend("topright", c("det ahist", "det hist", "sto ahist", "sto hist"),
col = c("black", "orangered", "grey", "darkred"), pch = 15, bty = "n")
```

Fecundity makes little difference in all cases, but the importance of stasis transitions drops a bit in historical analysis, while growth transitions increase a bit in importance. Next, we can see which historical transitions are most important.

```
<- cbind.data.frame(tm3elas_sums$hist[,2], tm3elas_s_sums$hist[,2])
elas_hist2plot names(elas_hist2plot) <- c("det hist", "sto hist")
rownames(elas_hist2plot) <- tm3elas_sums$hist$category
par(mar = c(7, 4, 2, 2) + 0.2)
barplot(t(elas_hist2plot), beside = T, ylab = "Elasticity", xlab = "", xaxt = "n",
col = c("orangered", "darkred"), bty = "n")
text(cex=1, x=seq(from = -0.5, to = 2.8*length(tm3elas_sums$hist$category), by = 2.85),
y=-0.06, tm3elas_sums$hist$category, xpd=TRUE, srt=45)
legend("topright", c("det ahist", "det hist", "sto ahist", "sto hist"),
col = c("orangered", "darkred"), pch = 15, bty = "n")
```

We can see that growth from time *t*-1 to *t* followed by shrinkage to time *t*+1 is associated with the greatest summed elasticities, while the inverse, shrinkage from *t*-1 to time *t* followed by growth to time *t*+1 is the next most important. Transitions associated with fecundity are associated with the lowest summed elasticities.

Further analytical tools are being planned for `lefko3`

, but packages that handle projection matrices can typically handle the individual matrices produced and saved in `lefkoMat`

objects in this package. Differences, obscure results, and errors sometimes arise when packages are not made to handle large and/or sparse matrices - historical matrices are both, and so care must be taken with their analysis.

We are grateful to two anonymous reviewers whose scrutiny improved the quality of this vignette. The project resulting in this package and this tutorial was funded by Grant-In-Aid 19H03298 from the Japan Society for the Promotion of Science.

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